<<

cells

Review Dysfunctional through the YAP/TAZ/Hippo Pathway as a Feature of Chronic Disease

1, 2, 2,3, 4 Mathias Cobbaut †, Simge Karagil †, Lucrezia Bruno †, Maria Del Carmen Diaz de la Loza , Francesca E Mackenzie 3, Michael Stolinski 2 and Ahmed Elbediwy 2,* 1 Phosphorylation Lab, Francis Crick Institute, London NW1 1AT, UK; [email protected] 2 Department of Biomolecular Sciences, Kingston University, Kingston-upon-Thames KT1 2EE, UK; [email protected] (S.K.); [email protected] (L.B.); [email protected] (M.S.) 3 Department of Chemical and Pharmaceutical Sciences, Kingston University, Kingston-upon-Thames KT1 2EE, UK; [email protected] 4 Epithelial Biology Lab, Francis Crick Institute, London NW1 1AT, UK; [email protected] * Correspondence: [email protected] These authors contribute equally to this work. †  Received: 30 November 2019; Accepted: 4 January 2020; Published: 8 January 2020 

Abstract: In order to ascertain their external environment, cells and tissues have the capability to sense and process a variety of stresses, including stretching and compression forces. These mechanical forces, as experienced by cells and tissues, are then converted into biochemical signals within the cell, leading to a number of cellular mechanisms being activated, including proliferation, differentiation and migration. If the conversion of mechanical cues into biochemical signals is perturbed in any way, then this can be potentially implicated in chronic disease development and processes such as neurological disorders, and obesity. This review will focus on how the interplay between mechanotransduction, cellular structure, metabolism and signalling cascades led by the Hippo-YAP/TAZ axis can lead to a number of chronic diseases and suggest how we can target various pathways in order to design therapeutic targets for these debilitating diseases and conditions.

Keywords: Hippo; YAP; TAZ; polarity; cancer; mechanotransduction; obesity; aPKC; neurodegenerative disease; talin;

1. Mechanotransduction: Overview and Structural Basis The ability of cells to detect and react to changes in their microenvironment is critical for the maintenance of both cellular function and tissue homeostasis [1,2]. Recent studies have expanded our understanding of a cell’s ability to sense its physical surroundings and respond to these stimuli to initiate the activation of intracellular signalling pathways that trigger downstream events [1,3]. Indeed, living cells are constantly in contact with mechanical cues and can translate the mechanical forces experienced in their environment into biochemical and behavioral responses. Cells can react to these forces through specific basal and transduce this into a process known as mechanotransduction [2,4,5]. Mechanotransduction is a process initiated by mechanically induced changes in protein conformation which result in cytoskeleton rearrangements, control and differentiation. The mechanical forces experienced by the cell are processed into biochemical signals to ultimately control expression, cell shape and cell fate [6]. The cell’s response to mechanical cues within the environment requires the cell’s ability to both transmit and generate forces. This occurs through basal interactions with the cellular (ECM) and cell-cell interactions with neighbouring cells through specialized transmembrane proteins [1,2]. Mechanotransduction is crucial for many cellular functions

Cells 2020, 9, 151; doi:10.3390/cells9010151 www.mdpi.com/journal/cells Cells 2020, 9, 151 2 of 17 such as cell adhesion, motility, migration, proliferation, differentiation and survival. If abnormalities in mechanotransduction occur this can for example lead to aberrant cell behavior and activation of key signalling pathways to drive phenotypical switching into more mesenchymal-like cancer cells from normal cells [4,7]. Cells are physically connected to the ECM through the transmembrane receptors protein family of integrins focal adhesion (FA-related proteins). External mechanical signals are sensed at FAs and translated into biochemical information through -related signalling pathways for maintaining proper cellular functions in cell shape, migration and survival [8]. Integrin activation is required for the normal functionality of cell adhesion, migration and extracellular matrix assembly. Integrins are a family of heterodimeric proteins comprising alpha and beta subunits that are activated through modulation of the cytoplasmic tail of integrin subunits and this activation is regulated by various biochemical signalling pathways. Besides their requirement for normal cellular mechanosensing, tumor cell migration, invasion, growth and metastasis are also regulated by abbrerant integrin-mediated mechanical signals [9,10]. One of the most extensively studied set of of recent times and a potent mechanosensor in are Yes-associated protein (YAP) and its homologous protein Transcriptional Co-Activator With PDZ-Binding Motif (TAZ). YAP/TAZ are sensors of structural and mechanical features of the cell microenvironment that are regulated by soluble extracellular factors, cell-to-cell adhesion and mechanotransduction [11,12] and play a central role in delivering mechanical cues from surrounding cells to the transcriptional machinery of the nucleus [13,14]. YAP and TAZ function as transcriptional co-activators shuttling between the cytoplasm and nucleus to induce the expression of cell-proliferative and anti-apoptotic by interacting with transcription factors, especially the TEA domain family members (TEAD) [12]. Although YAP is cytoplasmic at high cell density, the loss of cell contact with neighbouring cells or cell spreading results in YAP translocation to the nucleus. The expansion of cell contacts spreading over their basal substrate, the strength of the substrate and resulting mechanical tension are the key determinants of subcellular YAP localization in response to cell density [11,15,16]. Mechanotransduction affects YAP both independently of the canonical Hippo signalling pathway and with the involvement of key Hippo signalling pathway MST and LATS. Signalling cascades downstream of integrins are known to regulate YAP and TAZ activation [17–19]. Most of the main mechanosensitive induced through YAP/TAZ lean on integrin-mediated adhesion [11]. YAP and TAZ can also be directly regulated by the extracellular matrix (ECM) stiffness and YAP itself is involved in FA assembly [15,20,21] (Figure1). Mechanosensing the alterations of ECM stiffness can also be a causal input driving aberrant cell behaviours. The stiffness of ECM is a universal mechanical cue which control’s the preference of a cell between its choice of proliferation and death [16]. When cells perceive stiffness in the ECM, they change their spread and migration potential accordingly. YAP/TAZ activity is also regulated in this scenario. As mentioned, YAP and TAZ are activated by a stiff ECM and stretched cell shape in contrast to inhibition by a soft ECM environment and round cell shape [11,14,16,22,23]. Cells cultured on highly stiff ECM display activated YAP/TAZ with high nuclear localization and subsequent transcriptional activity, whereas cells arrest when YAP/TAZ is inhibited and relocalised to the cytoplasm on a soft ECM. In stiffer ECM, cells continue to proliferate and execute invasive phenotypes by increasing the expression and activity of adhesion receptors and thereby mechanotransduction pathways [11,14–16]. Another key regulator of mechanotransduction in relation to its environment is cellular polarity, which we will discuss in the next section. Cells 2020, 9, 151 3 of 17 Cells 2020, 8, x 3 of 17

FigureFigure 1. The 1. The regulation regulation ofof YAP at at the the level level of the of extrace the extracellularllular matrix involves matrix various involves proteins various involved proteins involvedin stabilizing in stabilizing and activating and activating YAP. In YAP.tegrins Integrins sense the sense external the externalforces an forcesd transmit and this transmit signal thisto talin signal to talin familyfamily membersmembers which which allow allow YAP YAP and and accessory accessory proteins proteins to act toas mechanosensors act as mechanosensors within the within cell. the cell.

2. Mechanotranduction2. Mechanotranduction and and Cell Cell Polarity Polarity Cell polarizationCell polarization is an essentialis an essential function function of several of several cell types cell types including including epithelial epithelial cells cells and migratoryand cells. Thismigratory part ofcells. the This review part willof the focus review on thewill interplay focus on betweenthe interplay cell polaritybetween cell and polarity mechanical and cues. mechanical cues. Cell polarity can occur along several axes, including an anterio-posterior (A–P) axis Cell polarity can occur along several axes, including an anterio-posterior (A–P) axis (e.g., in migratory (e.g., in migratory cells and neurons), and apicobasal and planar axes (e.g., in epithelia). In epithelia cells andand neurons),other cell types, and apico-basal apicobasal polarity and planar is the consequence axes (e.g., inof epithelia).localization and In epitheliaactivity of andmutually other cell types,antagonizing apico-basal complexes, polarity is including the consequence the Par, Crumbs of localization and Scribble and complexes activity (for of reviews mutually see antagonizing[24,25]). complexes,The Par including proteins are the segregated Par, Crumbs along andthe apico-basal Scribble complexes axis in epithelia (for with reviews an apical see [Par24, 25complex]). The Par proteinsconsisting are segregated of Par6/Par3/aPKC along the apico-basaland a basolateral axis in complex epithelia consisting with an of apical Par1/4/5. Par complexAt the apical consisting of Par6membrane/Par3/aPKC aPKC and activity a basolateral functions complex to activate consisting apical polarity of Par1 substrates/4/5. At theand apical restrict membrane activity of aPKC activitybasolateral functions proteins to activate and apicalconversely, polarity Par-1 substrates mediates andkinase restrict activity activity at the ofbasolateral basolateral membrane proteins and where aPKC is excluded [26]. In the C. elegans zygote, a similar distribution of Par proteins is observed conversely, Par-1 mediates activity at the basolateral membrane where aPKC is excluded [26]. along an A/P axis. Here polarity is a result of mechanical cues exerted by cytoskeletal components. In theIndeed,C. elegans the zygote,differential a similar diffusion distribution of Par proteins of Par is proteinsa consequence is observed of actomyosin along an contractions A/P axis. Here polarityorchestrated is a result by of the mechanical oocyte maturation; cues exerted coinciding by with cytoskeletal a cue originating components. from the Indeed, centrosome, the which differential diffusioncauses of a Par cortical proteins flow [27,28]. is a consequence This flow redistributes of actomyosin Par3 to contractions the anterior side orchestrated via a process by called the oocyte maturation; coinciding with a cue originating from the centrosome, which causes a cortical flow [27,28]. This flow redistributes Par3 to the anterior side via a process called advection. The activity of the redistributed Par proteins in this manner allows for chemical amplification of A/P identity and polarization. Mechanical cues are sufficient for other cells to polarize along an axis as well. For example, Cells 2020, 9, 151 4 of 17 in an attempt to find the minimal requirement for polarization of fibroblasts it was recently shown that a single point of adhesion with an above-threshold force to a fibronectin coated bead is enough to cause redistribution of the actomyosin structure and repositioning of the centrosome, supporting polarized behaviour [29,30]. In migratory cells mechanical force also induces polarization by formation of a single leading edge and suppressing of other protrusions by means of sensing membrane tension. This has been elegantly shown in neutrophils, where a leading edge protrusion characterized by increased membrane tension exerts long range inhibition on the rest of the cell, as measured by reduced Rac activity and SCAR/WAVE complex formation. This long-range inhibition is purely the result of a mechanical stimulus since application of membrane tension by applying a sucking force with a micropipette at one end of the cell causes the described effects [31]. Polarity proteins have also been involved in mechanosensing and altering the mechanical properties of cells. For example, aPKC activity has been linked to remodelling of the keratin intermediate filament (KIF) network in lung epithelial cells upon shear stress by phosphorylation of keratin at the phosphosite Ser-33, promoting its interaction with 14-3-3 [32]. Furthermore, aberrant aPKC signalling is oncogenic and elevated expression levels of aPKC have been observed in several [33–36]. Besides loss of polarity, overexpression of aPKC in cancer has also been implicated in altering the mechanical properties of cells. Indeed, spheroids consisting of MCF10A cells expressing aPKC have been observed to have increased surface tension [37]. Furthermore junctions between aPKC expressing and non-aPKC expressing cells bear an increased tension that allow them to actively extrude into the lamina [37]. Localization of polarity proteins also induces changes in local cytoskeletal composition. For example, Rho-GTPases such as Cdc42 and Rac stimulate actin nucleators and suppress destabilizing factors. Additionally, dynein pulling motors are regulated by the PAR polarity proteins in A/P polarized cells, where inhibition occurs at the anterior pole, resulting in pulling of the mitotic spindle towards the posterior pole [38,39]. Specifically aPKC has been implicated in phosphorylation of LIN5 inhibiting microtubule pulling force [40]. Mechanical cues and polarity have also been interlinked in higher order morphogenesis. For example in the C. elegans embryo, planar polarity of the apical Par module in the epidermis is established through muscle contractions that are relayed to the epidermal tight junctions via integrins and ECM components and hemidesmosomes [41]. Coupling of polarity to altering mechanistic properties has also been observed in fly follicles, where egg chamber rotation and elongation are an important part of maturation. Cetara and co-authors show in a recent paper that the elongation of the egg chamber is dependent on the planar alignment of actin fibers at the basolateral membrane [42]. They further show that loss of egg rotation disturbs this planar alignment, likely due to the fact that polarity information cannot be transmitted to the expanding epithelium surrounding the egg, but the exact mechanism has not been elucidated. Several polarity proteins also induce signalling to the Hippo pathway and YAP/TAZ itself. It has been shown that the apical Crumbs can associate with FERM domain-containing protein 6 (FRMD6), Kibra and composing a scaffold that activates the Hippo pathway [43–45]. Furthermore YAP is also supressed by the tight junction binding protein AMOTS [46–48] and by binding to α-catenin at adherens junctions [49,50]. In contrast, aPKC and the Par complex have been shown to drive nuclear YAP signalling. In epithelial cells overexpression of activated aPKC causes loss of contact inhibition and overgrowth by uncoupling MST1/2 from LATS1/2, causing nuclear accumulation of YAP. Additionally in MDCK cells specifically, downregulation of AMOTS expression also caused a loss of YAP localization to junctions and a spindle like [51]. Inactivation of the Hippo pathway has also been associated with elevated expression of Par-3 in metastatic prostate cancer by driving a KIBRA/Par-3/aPKC complex formation in lieu of the activating KIBRA/Merlin/FRMD6 complex [52]. Suppression of Hippo signalling by polarity is also seen in the developing embryo, where an inner cell mass is non-polarized and has a different fate then the surrounding trophectoderm which is polarized. This is achieved Cells 2020, 9, 151 5 of 17 by polarity signals that inactivate Hippo signalling and cause translocation of YAP to the nucleus, activating a TEAD-dependent transcriptional program (for a recent review see [53]). The Par complex Cells 2020, 8, x 5 of 17 seems to be important for at the 32-cell stage of embryonic development, whereas at the 16-cell stage Par-independentnon-polarized and mechanisms has a different are alsofate then involved the su [rrounding54]. trophectoderm which is polarized. This is Thereachieved seems by polarity to be asignals reciprocal that inactivate interplay Hippo between signalling polarity and cause andHippo translocation signalling of YAP since to the a recent geneticnucleus, screen activating looking a TEAD-depende for proteins inntC. transcriptional elegans that are program involved (for ina recent maintenance review see of [53]). cell polarityThe Par in the growingcomplex intestine seems to implicated be important several for at components the 32-cell stage of the of embryonic Hippo pathway development, including whereas YAP at and the TEAD 16- [55]. cell stage Par-independent mechanisms are also involved [54]. It thus seems that the regulation of Hippo signalling by polarity is dependent on the order of There seems to be a reciprocal interplay between polarity and Hippo signalling since a recent genetic events during polarization, the different polarity complexes formed and thus the level and molecular screen looking for proteins in C. elegans that are involved in maintenance of cell polarity in the growing tuningintestine of the implicated respective several proteins, components a regulation of the Hippo which pathway seems including to include YAP and a feedback TEAD [55]. control from the Hippo pathwayIt thus seems itself. that How the regulation these polarity of Hippo cues signalling are linked by polarity to mechanical is dependent signals on the that order act of on events the Hippo pathwayduring needspolarization, to be the elucidated different polarity further, complexes but because formed of and the thus close the interplay level and molecular between tuning the two, of some cross-regulationthe respective proteins, is inevitable. a regulation which seems to include a feedback control from the Hippo pathway itself.In conclusion How these polarity it is emerging cues are linked that mechanicalto mechanical stimulisignals that and act polarity on the Hippo are closelypathway interlinked, needs to be both at theelucidated level of further, individual but because cells of as the well close as interplay at the levelbetween of the two, developing some cross-regulation tissue. While is inevitable. some systems like the InC. conclusion elegans zygote it is emerging have been that extensively mechanical studied,stimuli and many polarity of the are mechanisms closely interlinked, regarding both couplingat the level of individual cells as well as at the level of the developing tissue. While some systems like of mechanical to chemical stimuli have yet to be resolved. Loss of polarisation can lead to cellular the C. elegans zygote have been extensively studied, many of the mechanisms regarding coupling of transformation and epithelial to mesenchymal transition, a tumour-initiating process. The next section mechanical to chemical stimuli have yet to be resolved. Loss of polarisation can lead to cellular willtransformation explore the link and between epithelial mechanotransduction to mesenchymal transition, and disease. a tumour-initiating process. The next section will explore the link between mechanotransduction and disease. 3. Mechanotransduction Signalling in Disease 3.Mechanotransduction Mechanotransduction Signalling is an important in Disease cellular hallmark in the formation of chronic disease. Loss ofMechanotransduction polarity or mechanosensing is an important can leadcellular to hallmark a range in of the diseases formation including of chronic cancer, disease. obesity Loss and neurodegenerativeof polarity or mechanosensing diseases and variouscan lead pathways to a range can of be diseases involved includ in thising process.cancer, obesity Figure 2and provides an overviewneurodegenerative of the types diseases of signalling and various pathways pathways involved can be involved in these in diseases this process. and Figure we shall 2 provides discuss this in morean detailoverview in theof the coming types of section. signalling pathways involved in these diseases and we shall discuss this in more detail in the coming section.

FigureFigure 2. 2.The The pathways pathways andand interplay with with regulate regulate me mechanotransductionchanotransduction in the in context the context of chronic of chronic disease and polarity. Note that some pathways are not well established and thus represented by a disease and polarity. Note that some pathways are not well established and thus represented by question mark (?) (T2D = Type 2 Diabetes). Please note also ⟶ = activates and —| = inhibits. a question mark (?) (T2D = Type 2 Diabetes). Please note also = activates and —| = inhibits. → Cells 2020, 9, 151 6 of 17

3.1. Cancer Solid tumors exhibit increased ECM stiffness and crosslinking that promote an invasive phenotype in cancer cells. Increased stiffness of the ECM can also lead to a disruption of the epithelial polarity resulting in migration and metastasis [4]. In addition, stiff ECM activates the β1-integrin-FAK-Src-PI3K-PDK1 pathway to facilitate YAP nuclear translocation and transcriptional activation as previously discussed [11,56,57]. Concomitantly, YAP/TAZ is overexpressed and highly accumulated in the nuclei of cancer cells, initiating the transcription of YAP/TAZ target genes to drive proliferation, invasion and metastasis [13]. Thus, YAP/TAZ plays a crucial role in driving tumorigenesis as dysregulation of the Hippo pathway and sustained activation of YAP drives uncontrollable growth [58]. There is scope for further investigations in the future of the role of novel ECM components and how they relate to Hippo pathway signalling. We have already previously identified a family of ECM cross-linkers (Enigma family members) which link the ECM to the cytoskeleton and result in the regulation of YAP [16]. It has also been shown that the mechanical regulation of the Hippo pathway is conserved in a wide range of species [59–61]. Mechanotransduction could play a potentially important role in the development of targeted therapies targeting the cancer cell’s pro-proliferative and survival signals stemming from its interaction with the stroma. An example of such a target could be the talin family of proteins. Extensive biological studies have hinted that the talin family of proteins may play an important role in the transduction of the integrin signal. Talins are a major cytoskeletal protein at focal adhesions that link intracellular networks with the ECM via its coupling with the actin cytoskeleton and membrane integrins [9,10,62,63]. Talins are comprised of a globular head and a long rod domain. The FERM domain within the talin head domain provides a binding site to the cytoplasmic integrin β subunit whereas the C-terminal talin rod containing several vinculin binding sites provides a connection to the actin cytoskeleton and the ECM within the cell suggesting that talin is an important mechanosensitive molecule [2,64,65]. In vertebrates, there are two talin genes: talin1 and talin2. The talin1 protein was found to regulate focal adhesion dynamics, cell migration and invasion; whereas the precise role of the talin2 protein in cancer is not clear. Talin1 is expressed in nearly all tissues whereas talin2 is mainly expressed in the heart, brain, testis and muscles [66]. Talin2 functions distinctly from talin1 in the regulation of cell invasion and is usually localized at large focal adhesions and fibrillary adhesions. In the absence of talin1, talin2 was found to regulate focal adhesion assembly and focal adhesion kinase signalling [67]. Interestingly, the talin2 head domain (TH2) has a higher affinity and a much stronger binding to β-integrin tails than talin1 head domain (TH1) which is important for traction force generation and cell invasion (Figure1). The strong binding of talin2 with the β-integrin tail produces the aforementioned traction force which goes on to colocalise with invadopodia and encourages invadopodium-mediated matrix degradation. This is a key mechanism for cancer cell invasion [67]. In breast cancer cell lines, talin2 controls production of traction force through its strong binding with β-integrins thus leading to the regulation of various processes including cell migration, invasion, tumor growth and metastasis and potentially oncogenic activation of various proteins [10]. The talin family has also been linked to obesity since talin levels increase with increasing adipose cell size in the growing fat pad. The next section further explores the link between mechanotransduction and adipose regulation.

3.2. Obesity In addition to chemical and hormonal influences, mechanotransduction signals play an important role in adipogenesis. These mechanical cues as well as having an important role in adipocyte development, also play a major role in differentiation to adipogenic lineages [68]. A combination of all of these influences, in addition to distinct precursor populations of adipocytes, together with final tissue location influencing functionality, results in specific depot physiology for the prevailing adipose tissue mass formed [69,70]. Cells 2020, 9, 151 7 of 17

The number of adipocyte cells in adults appear to be relatively fixed, even after weight loss, with large variations in cell size both within and between individuals. A stable number of cells and an approximate 10% turnover annually, which is not influenced by energy balance, indicates a tight regulatory control of the accumulated tissue mass formed [71,72]. This is of importance in the context of obesity and the resulting pathology caused by dysregulation of whole body metabolism and insulin resistance. The physiological response to excess calorie intake is adipocyte lipid loading, causing an increased cell volume. This propagates the metabolic complications of obesity. Indeed, enhanced accumulation of lipid may lead to adipocyte hypertrophy, characteristic of adipose tissue dysfunction [73]. Adipocytes store lipids in the form of triacylglycerides in a single, large unilocular lipid filled droplet. The consequence of this is an increase in the stiffness of the adipocyte [74]. This stiffness adds to mechanical stress such as different loading or weight bearing strains which also generate forces which adipocytes are exposed to. The resultant mechanical forces can be transduced to affect adipogenesis [75]. These forces are transduced by various protein complexes such as: focal adhesions interconnecting with the actin cytoskeleton [76] or ion channels that are sensitive to mechanical stress [77]. In line with this, a recent study has identified a volume sensitive on the adipocyte surface which can regulate insulin signalling [78]. This protein, SWELL1, is increased in human hypertrophic adipocytes of obese and is required for glucose uptake via PI3K-AKT2-GLUT4 signalling activity. This provides evidence of a link between mechanoreception and insulin signalling which is activated under obesogenic conditions. Following transduction, static or dynamic forces which alter adipocyte cell shape or the adipocyte microenvironment have been shown to activate various intracellular pathways including RhoA/ROCK, Akt/Erk and the Hippo pathway which influence gene expression and cell fate [79]. Chronic mechanical force such as that exerted through extracellular matrix stiffness, as occurs through the development of adipose tissue fibrosis, has been associated with metabolic complications in obesity. Evidence for this has been provided through the preparation of 3D adipocyte hydrogel cultures with incorporated decellularized material from the adipose tissue of obese subjects. This induced dysfunctional adipocyte metabolism and increased expression of connective tissue (CTGF) through the Hippo related YAP/TEAD-dependent pathway [80]. A cells metabolic status plays an important role in regulating key members of the Hippo pathway, YAP and TAZ. These factors have both been shown to regulate and be regulated by multiple metabolic pathways and energy-sensing pathways such as via AMP-activated (AMPK) [81–84]. The master regulator of metabolism and proliferation, c-, which itself is influenced by growth factor and nutrient availability, has been shown to be influenced by components of the Hippo pathway [85]. It has been shown that adipocyte proliferation may be activated by the SIRT1/c-Myc pathway. Reduced levels of SIRT1 resulted in hyperacetylated c-Myc which promoted the formation of a metabolically dysfunctional 3T3-L1 preadipocyte phenotype [86]. Within adipocytes, the activity of one of the key transcriptional factors for adipogenesis, PPARy is suppressed by TAZ. In this regard, adipose-specific TAZ knockout mice show improvements in insulin sensitivity and glucose metabolism, establishing a potential role for TAZ in promoting insulin resistance [87]. Liraglutide, a GLP-1 analogue and antidiabetic agent also used to treat obesity, has shown to activate the Hippo pathway by increasing YAP related pathway components (MST1, LATS1 and p-YAP). This results in reduced but increased cell differentiation of 3T3-L1 preadipocytes [88]. These studies suggest crucial connections with the regulation of substrate metabolism and the Hippo pathway. It is therefore key to establish the mechanisms for cross-talk between mechanotransduction pathways such as the Hippo pathway and substrate metabolism, tissue expansion, the development of adipocyte hypertrophy and insulin resistance. Obesity is a risk factor for cancer development, and a recent research focus has provided evidence that this link may be partially due to alterations in the Hippo pathway. Of interest is that adipocytes form a major component of the tumour microenvironment in for example breast, colon and gastric Cells 2020, 9, 151 8 of 17 cancers and can therefore directly contribute to cancer cell development [89,90]. Obesity has been shown to accelerate cancer development following the subcutaneous injection of murine forestomach carcinoma cells. This was shown to act through the influence of the adipokine visfatin whose concentration in serum was correlated with SIRT1 (a multifunctional protein that regulates metabolic activity). The upregulated SIRT1 promoted YAP2/TEAD4 activation and the development of cancer in a diet-induced murine obesity model [91]. Obesity and insulin resistance are also important risk factors for the development of endometrial cancer where knockdown of YAP/TAZ has been shown to inhibit insulin signalling via phosphorylation of IRS1/2, a mediator of insulin and IGF-1 signalling in endometrial cell lines [92]. The Hippo pathway may therefore represent a novel target for cancer prevention where adipocytes are closely associated with cancer such as breast cancer [93,94] or where insulin resistance is associated with cancer progression [95]. One strategy for treating obesity has been through inducing a switch from white to brown like (beige) adipocytes, which can arise postnatally in white adipose tissue depots. Beige adipocytes, which dissipate energy as heat as opposed to storing fat, can be induced by various cues including temperature, exercise, adrenergic stimulation, nutritional and hormonal signals [96]. These adipocytes are associated with increased energy expenditure and improved insulin sensitivity, similar to brown adipocytes. Understanding how beige selective pathways are induced can provide new insights that could allow for the targeted selection of this metabolically favorable phenotype of adipocyte. Although developmentally of different origin (muscle-like), YAP/TAZ signalling has also been shown to regulate insulin signalling in muscle where TAZ has shown to stimulate insulin sensitivity by upregulating IRS1 which mediates GLUT4 uptake of glucose in muscle cells [97]. Brown adipocytes (BAT) are functionally similar to beige adipocytes. Both cell types show multilocular deposition of lipid and increased oxidative metabolism through upregulation of UCP1, which induces thermogenesis. It is therefore of interest that BAT development is dependent on YAP/TAZ signalling which upregulates UCP1 expression and that this process is mediated through a cytoskeletal mechanotransduction response [98]. Understanding the role of adipocytes in the context of obesity related disease processes, including cancer, and uncovering tissue-specific molecules related to the functioning of the Hippo pathway could provide biomarkers or targets for therapy. However, the association of the Hippo pathway with multiple functions associated with growth and development in tissues also provides a challenge with respect to potential side effects.

3.3. Neurodegenerative Disease The sensory processes of hearing, touch, and pain sensation depend on transducing certain types of mechanical force into sensory information. Sensory disorders involving dysfunction of these processes have been identified (such as deafness) [99]. However, additionally, sensing and transduction of other local tissue mechanical forces are critical for normal neuronal development, homeostasis, and function. In the developing embryonic nervous system, neuronal progenitors migrate, and neuronal axons extend, branch, and find their synaptic targets through various embryonic tissue types [100]. In normal adult function, neurons are also under constantly changing mechanical forces due to the movement or pressure of surrounding muscles or tissues, especially during tissue damage. Stretching of neurons, such as during regenerative axon growth, is known to promote neurite outgrowth and to be a potent regulator of axon growth. Much is now known of the general molecular and biochemical pathways governing neuronal development, function and disease. However, the specific roles of mechanical forces in neuronal homeostasis and function have only recently started to be determined. For example, retinal ganglion axons prefer to grow through ‘softer’ tissue and avoid ‘stiffer’ tissue in Xenopus brains [101]. A wide variety of proteins with links to mechanotransduction have been identified as important to neuronal development and function/homeostasis, including mechanosensitive Piezo ion channels (e.g., Piezo-1, Piezo-2), transient potential (TRP) channels (e.g., TRPV2, TRPV4), transmembrane or Cells 2020, 9, 151 9 of 17 extracellular matrix (ECM) proteins (e.g., integrins, β-spectrin), and intracellular signalling proteins (e.g., YAP/TAZ). Despite this, even less is known of the importance or role of mechanotransduction in the development or progression of neurodegenerative diseases (NDD). Changes in the ECM and/or tissue stiffness have been reported in traumatic brain injury and brain cancer [102] and in central nervous system glial scars in rats [103] but also in Alzheimer’s disease [104,105], Parkinson’s disease [106], and multiple sclerosis [107], suggesting that stiffness changes may be relevant to NDD. Several recent studies have provided intriguing evidence that mechanotransduction proteins may also have fundamental direct roles in neurodegenerative disease. Piezo-1 is a mechanically gated calcium channel mainly expressed on the of myelinated neurons and, as it responds to mechanical stimuli, it plays an important role in mechanotransduction [108]. On activation by traction forces, Piezo-1 allows the entrance of calcium ions (Ca2+) into the cell. Activation of Piezo-1 in neuronal stem cells induces their differentiation into neurons, rather than astrocytes [109]. Furthermore, Piezo-1 activation results in the nuclear targeting of YAP and TAZ, an event implicated in the formation in the central nervous system (CNS) [109]. Disorders involving progressive demyelination (loss of myelin), called demyelinating disorders can lead to axonal injury, neurodegeneration, and significant disability and death [110,111]. Demyelinating disorders are often characterised by an axonal Ca2+ imbalance, resulting in an increased influx of Ca2+, thus causing elevated production of reactive oxygen species and excitotoxicity [112]. In a recent study, enhancing Piezo-1 activation with a small-molecule agonist Yoda-1 caused axon demyelination in mouse cerebellar slices, while a pharmacological Piezo-1 inhibitor, GsMTx4, caused increased myelin formation [108]. It was hypothesised that over-activation of Piezo-1 induces increased influx of Ca2+ into CNS axons, release of Ca2+ from intracellular stores, and activation of calpain, a protease that can cleave talin and modify integrin-mediated cell adhesion [108]. For this reason, blocking Ca2+ influx by inhibition of the Piezo-1 Ca2+ channel might have therapeutic implications in demyelinating and neurodegenerative disorders. Furthermore, GsMTx4 attenuated axonal damage induced by demyelination and reduced microglial reactivity following activation by LPS (lipopolysaccharide) [108]. Piezo-1 expression in amyloid plaque-reactive astrocytes is also upregulated by peripheral bacterial infection in rats [113]. As microglial reactivity and/or other immune mechanisms are thought to facilitate neurodegeneration, and are implicated in Alzheimer’s disease progression, this further suggests the potential beneficial use of Piezo-1-modulating agents in treating neurodegenerative disease. Further evidence of mechanotransduction changes in neurodegeneration disease through the YAP/Hippo pathway has recently been provided. Alexander disease (AxD) is a rare neurodegenerative disease of primary astrocyte dysfunction which features gain-of-function mutations in and protein aggregations of the astrocytic protein GFAP [114]. A Drosophila AxD model overexpressing a human mutant form of GFAP (GFAPR79H) showed activation of the YAP/Hippo pathway, with resulting abnormal changes to mechanotransduction proteins including lamin, focal adhesion kinase (FAK) and ECM proteins, leading to behavioural abnormalities and neurodegeneration in this fly model [114]. Furthermore, brains of transgenic AxD mice showed increased tissue stiffness and iPSC-derived astrocytes from one AxD patient displayed increased A-type lamin and nuclear-localised YAP compared to control astrocytes [114]. Interestingly, a neuronal-specific isoform of YAP,YAPdeltaC, protects against neuronal in a model of the neurodegenerative disease Huntington’s disease (HD), by blocking interaction of full-length YAP with [115], and was recently shown to modulate neurodegeneration in a mouse model of spinocerebellar ataxia 1 [116]. Additionally, activation of MST1 is increased in human post-mortem HD cortex, and nuclear localisation of YAP is correspondingly decreased in human HD cortex and in neuronal stem cells derived from HD patients (117), leading to altered Hippo pathway gene expression [117]. The YAP/TAZ/Hippo pathway may therefore be a relevant mechanism in mammalian neurodegenerative processes, and perhaps particularly in aggregation-prone neurodegenerative diseases. Cells 2020, 9, 151 10 of 17

Finally, glaucoma is an ocular disease featuring increased intraocular pressure (IOP), which when untreated leads to retinal damage, the irreversible degeneration of retinal ganglion cell (RGC) neurons, and blindness [118]. A number of mechanotransduction mechanisms and proteins have been implicated in the various anatomical and physiological changes in the eye which lead to glaucoma and, as a secondary consequence, RGC degeneration. Interestingly, however, the mechanosensitive ion channels TRPV4 and TREK-1, as well as integrins, have been suggested to be directly involved within RGC in pressure-induced dendritic retraction and RGC loss, in glaucoma [119], through sensing stretch, compression, tension and/or shear of retinal or retinal-associated ocular components. TRPV4 is strongly expressed in RGCs, and induction of TRPV4 causes RGC degeneration and other related ocular pathologies in mice and in vitro [119]. As mice with ablated TRPV4 or TREK genes show reduced and increased sensitivity to mechanical stress, respectively [120,121], these channels may act in opposition to regulate homeostatic responses to mechanical stress in the retina. Interestingly, TRPV4 activation causes YAP/TAZ nuclear translocation during cellular epithelial-mesenchymal transition (EMT) in keratinocytes [122,123]. It will be useful to identify if TRPV4 also effects this process in retinal ganglion cells. Further, aging is a risk factor for glaucoma, as well as other NDD. Many components of the eye undergo tissue stiffening and ECM remodelling in older age [124]. Age-related changes in tissue stiffness may be a relevant avenue for further investigation in NDD development. In summary, the large number of mechanosensing proteins that have critical roles in neural development and function/maintenance suggests that further roles for these proteins in NDD will likely be discovered.

4. Conclusions As we have conveyed, mechanotransduction plays a huge role in a wide range of cellular and physiological processes of which the dysregulation can contribute to a number of chronic diseases including obesity, diabetes, cancer (including loss of polarity/tissue context) and neurodegenerative disease. Table1 summarises the key pathways shown in this review, important proteins from these pathways and how these proteins are implicated in a number of diseases.

Table 1. Proteins discussed in this review involved in mechanotransduction and diseases associated with their dysfunction.

Pathway Protein Disease References Extracellular matrix Integrins Cancer [9,10] (ECM) Talin2 Cancer [10,66] Alexander disease [114] Huntington’s disease [115] YAP Spinocerebellar ataxia 1 [116] Hippo signalling Demyelinating disorders [109] Cancer [4] Cancer [13] TAZ Demyelinating disorders [109] Type 2 diabetes [87] Demyelinating disorders [108] Piezo-1 Ion channels Alzheimer’s disease [113] TRPV4 Glaucoma [119] Polarity aPKC Cancer (contributing) [37] UCP1 Obesity [98] Metabolic pathways IRS1 Cancer [92]

Many of these signalling pathways involved in the process of mechanotransduction (and thus tissue stiffness) seems to revolve around YAP/TAZ signalling. If YAP/TAZ which are established Cells 2020, 9, 151 11 of 17 mechanosensors can be inhibited by therapy then we can potentially affect the levels of chronic disease and tissue stiffening with increasing age. Future therapeutic options for targeting tissue stiffness will include targeting the Hippo pathway. As shown in Figure3, if therapy is initiated during increasing tissue sti ffness hypothetically we can reduce the incidence of the chronic disease. The interplay between mechanotransduction and chronic disease is a large field which we can explore with various targeted therapies with the ultimate goal of treating cases of chronic disease. Cells 2020, 8, x 11 of 17

Figure 3. A hypothetical graph linking the effect of tissue stiffness with age and chronic disease. Upon Figure 3. A hypothetical graph linking the effect of tissue stiffness with age and chronic disease. Upon therapy intervention which would target signalling cascades we would assume a correlation between therapy intervention which would target signalling cascades we would assume a correlation between less stiffness and chronic disease. less stiffness and chronic disease.

AuthorAuthor Contributions: Contributions: M.C.M.C. wrote the the polarity polarity section, section, S.K. S.K. and and A. A.E.E. wrote wrote the the cancer cancer section, section, introduction introduction and andconclusion, conclusion, L.B. M.S.and F.E.M. wrote wrote the obesity the neurodegenerative section, L.B. and disease F.E.M. section. wrote the The neurodegenerative review was conceived disease and planned section. Theby M.C., review M.S., was F.E.M., conceived M.D.C.D.d.l.L. and planned and by M.C.,A.E., Figures M.S., F.E.M., were M.D.C.D.d.l.L.designed by M.D.C.D.d.l.L. and A.E., Figures Manuscript were designed was proof by M.D.C.D.d.l.L. Manuscript was proof read by all the authors and corrected by A.E. All authors have read and agreedread by to all the the published authors versionand corrected of the manuscript.by A.E. All authors have read and agreed to the published version of the manuscript. Funding: We acknowledge support for the APC by the Francis Crick Institute, which receives its core funding fromFunding: Cancer We Research acknowledge UK (CRUK) support (FC001130), for the APC the by UK the Medical Francis Crick Research Institute, Council which (MRC) receives (FC001130), its core andfunding the Wellcome Trust (FC001130). from Cancer Research UK (CRUK) (FC001130), the UK Medical Research Council (MRC) (FC001130), and the ConflictsWellcome of Trust Interest: (FC001130).The authors declare no conflict of interest.

ReferencesConflicts of Interest: The authors declare no conflict of interest.

1.ReferencesShamsan, G.; Odde, D. Emerging technologies in mechanotransduction research. Curr. Opin. Chem. Biol. 2019, 53, 125–130. [CrossRef] 1. Shamsan, G.; Odde, D. Emerging technologies in mechanotransduction research. Curr. Opin. Chem. Biol. 2. Sun, Z.; Guo, S.; Fässler, R. Integrin-mediated mechanotransduction. J. Cell Biol. 2016, 215, 445–456. 2019, 53, 125–130. [CrossRef] 2. Sun, Z.; Guo, S.; Fässler, R. Integrin-mediated mechanotransduction. J. Cell Biol. 2016, 215, 445–456. 3. Chin, L.; Xia, Y.; Discher, D.; Janmey, P. Mechanotransduction in cancer. Curr. Opin. Chem. Eng. 2016, 11, 3. Chin, L.; Xia, Y.; Discher, D.; Janmey, P. Mechanotransduction in cancer. Curr. Opin. Chem. Eng. 2016, 11, 77–84. [CrossRef][PubMed] 77–84. 4. Maxwell, C.; Roskelley, C. Genomic Instability and Cancer Metastasis; Springer: Cham, Switzerland, 2015. 4. Maxwell, C.; Roskelley, C. Genomic Instability and Cancer Metastasis; Springer: Cham, Switzerland, 2015. 5. Seong, J.; Wang, N.; Wang, Y. Mechanotransduction at focal adhesions: From physiology to cancer development. J. Cell. Mol. Med. 2013, 17, 597–604. 6. Mohri, Z.; Del Rio Hernandez, A.; Krams, R. The emerging role of YAP/TAZ in mechanotransduction. J. Thorac. Dis. 2017, 9, E507–E509. 7. Aw Yong, K.; Sun, Y.; Merajver, S.; Fu, J. Mechanotransduction-Induced Reversible Phenotypic Switching in Prostate Cancer Cells. Biophys. J. 2017, 112, 1236–1245. 8. Kuo, J.C. Mechanotransduction at focal adhesions: Integrating Cytoskeletal. Mechanics in migrating cells. J. Cell. Mol. Med. 2013, 17, 704–712. 9. Tadokoro, S.; Shattil, S.; Eto, K.; Tai, V.; Liddington, R.; Pereda, J.; Ginsberg, M.; Calderwood, D. Talin Binding to Integrin Tails: A Final Common Step in Integrin Activation. Science 2003, 302, 103–106.

Cells 2020, 9, 151 12 of 17

5. Seong, J.; Wang, N.; Wang, Y. Mechanotransduction at focal adhesions: From physiology to cancer development. J. Cell. Mol. Med. 2013, 17, 597–604. [CrossRef][PubMed] 6. Mohri, Z.; Del Rio Hernandez, A.; Krams, R. The emerging role of YAP/TAZ in mechanotransduction. J. Thorac. Dis. 2017, 9, E507–E509. [CrossRef][PubMed] 7. Aw Yong, K.; Sun, Y.; Merajver, S.; Fu, J. Mechanotransduction-Induced Reversible Phenotypic Switching in Prostate Cancer Cells. Biophys. J. 2017, 112, 1236–1245. [CrossRef][PubMed] 8. Kuo, J.C. Mechanotransduction at focal adhesions: Integrating Cytoskeletal. Mechanics in migrating cells. J. Cell. Mol. Med. 2013, 17, 704–712. [CrossRef] 9. Tadokoro, S.; Shattil, S.; Eto, K.; Tai, V.; Liddington, R.; Pereda, J.; Ginsberg, M.; Calderwood, D. Talin Binding to Integrin Tails: A Final Common Step in Integrin Activation. Science 2003, 302, 103–106. [CrossRef] 10. Li, L.; Li, X.; Qi, L.; Rychahou, P.; Jafari, N.; Huang, C. The role of talin2 in breast cancer tumorigenesis and metastasis. Oncotarget 2017, 8, 106876. [CrossRef] 11. Chakraborty, S.; Njah, K.; Pobbati, A.; Lim, Y.; Raju, A.; Lakshmanan, M.; Tergaonkar, V.; Lim, C.; Hong, W. Agrin as a Mechanotransduction Signal Regulating YAP through the Hippo Pathway. Cell Rep. 2017, 18, 2464–2479. [CrossRef] 12. Borreguero-Muñoz, N.; Fletcher, G.C.; Aguilar-Aragon, M.; Elbediwy, A.; Vincent-Mistiaen, Z.I.; Thompson, B.J. The Hippo pathway integrates PI3K–Akt signals with mechanical and polarity cues to control tissue growth. PLoS Biol. 2019, 17, e3000509. [CrossRef][PubMed] 13. Li, P.; Silvis, M.R.; Honaker, Y.; Lien, W.-H.; Arron, S.T.; Vasioukhin, V. αE-catenin inhibits a Src-YAP1 oncogenic module that couples tyrosine kinases and the effector of Hippo signaling pathway. Genes Dev. 2016, 30, 798–811. [CrossRef][PubMed] 14. Halder, G.; Dupont, S.; Piccolo, S. Transduction of mechanical and cytoskeletal cues by YAP and TAZ. Nat. Rev. Mol. Cell Biol. 2012, 13, 591–600. [CrossRef][PubMed] 15. Nardone, G.; Oliver-De La Cruz, J.; Vrbsky, J.; Martini, C.; Pribyl, J.; Skládal, P.; Pešl, M.; Caluori, G.; Pagliari, S.; Martino, F.; et al. YAP regulates cell mechanics by controlling focal adhesion assembly. Nat. Commun. 2017, 8, 15321. [CrossRef][PubMed] 16. Elbediwy, A.; Vanyai, H.; Diaz-de-la-Loza, M.; Frith, D.; Snijders, A.; Thompson, B. Enigma proteins regulate YAP mechanotransduction. J. Cell Sci. 2018, 131, jcs221788. [CrossRef] 17. Elbediwy, A.; Thompson, B.J. Evolution of mechanotransduction via YAP/TAZ in epithelia. Curr. Opin. Cell Biol. 2018, 51, 117–123. [CrossRef] 18. Fan, R.; Kim, N.G.; Gumbiner, B.M. Regulation of Hippo pathway by mitogenic growth factors via phosphoinositide 3-kinase and phosphoinositide-dependent kinase-1. Proc. Natl. Acad. Sci. USA 2013, 110, 2569–2574. [CrossRef] 19. Ege, N.; Dowbaj, A.M.; Jiang, M.; Howell, M.; Hooper, S.; Foster, C.; Jenkins, R.P.; Sahai, E. Quantitative Analysis Reveals that Actin and Src-Family Kinases Regulate Nuclear YAP1 and Its Export. Cell Syst. 2018, 6, 692–708. [CrossRef] 20. Tan, F.; Huang, Y.; Pei, Q.; Liu, H.; Pei, H.; Zhu, H. Matrix stiffness mediates stemness characteristics via activating the Yes-associated protein in cells. J. Cell. Biochem. 2018.[CrossRef] 21. Shen, J.; Cao, B.; Wang, Y.; Ma, C.; Zeng, Z.; Liu, L.; Li, X.; Tao, D.; Gong, J.; Xie, D. Hippo component YAP promotes focal adhesion and tumour aggressiveness via transcriptionally activating THBS1/FAK signalling in breast cancer. J. Exp. Clin. Cancer Res. 2018, 37, 175. [CrossRef] 22. Rice, A.J.; Cortes, E.; Lachowski, D.; Cheung, B.C.H.; Karim, S.A.; Morton, J.P.; Del Río Hernández, A. Matrix stiffness induces epithelial-mesenchymal transition and promotes chemoresistance in pancreatic cancer cells. Oncogenesis 2017, 6, e352. [CrossRef][PubMed] 23. Dupont, S.; Morsut, L.; Aragona, M.; Enzo, E.; Giulitti, S.; Cordenonsi, M.; Zanconato, F.; Le Digabel, J.; Forcato, M.; Bicciato, S.; et al. Role of YAP/TAZ in mechanotransduction. Nature 2011, 474, 179–183. [CrossRef] 24. Assémat, E.; Bazellières, E.; Pallesi-Pocachard, E.; Le Bivic, A.; Massey-Harroche, D. Polarity complex proteins. Biochim. Biophys. Acta Biomembr. 2008, 1778, 614–630. [CrossRef][PubMed] 25. Rodriguez-Boulan, E.; Macara, I.G. Organization and execution of the epithelial polarity programme. Nat. Rev. Mol. Cell Biol. 2014, 15, 225–242. [CrossRef][PubMed] Cells 2020, 9, 151 13 of 17

26. Wang, S.-C.; Low, T.Y.F.; Nishimura, Y.; Gole, L.; Yu, W.; Motegi, F. Cortical forces and CDC-42 control clustering of PAR proteins for Caenorhabditis elegans embryonic polarization. Nat. Cell Biol. 2017, 19, 988–995. [CrossRef][PubMed] 27. Goehring, N.W.; Grill, S.W. Cell polarity: Mechanochemical patterning. Trends Cell Biol. 2013, 23, 72–80. [CrossRef] 28. Reich, J.D.; Hubatsch, L.; Illukkumbura, R.; Peglion, F.; Bland, T.; Hirani, N.; Goehring, N.W. Regulated Activation of the PAR Polarity Network Ensures a Timely and Specific Response to Spatial Cues. Curr. Biol. 2019, 29, 1911–1923. [CrossRef] 29. Das, A. A Critical Pull to Polarize the Cell. Biophys. J. 2014, 107, 285–286. [CrossRef] 30. Bun, P.; Liu, J.; Turlier, H.; Liu, Z.; Uriot, K.; Joanny, J.F.; Coppey-Moisan, M. Mechanical checkpoint for persistent cell polarization in adhesion-naive fibroblasts. Biophys. J. 2014, 107, 324–335. [CrossRef] 31. Houk, A.R.; Jilkine, A.; Mejean, C.O.; Boltyanskiy, R.; Dufresne, E.R.; Angenent, S.B.; Altschuler, S.J.; Wu, L.F.; Weiner, O.D. Membrane tension maintains cell polarity by confining signals to the leading edge during neutrophil migration. Cell 2012, 148, 175–188. [CrossRef] 32. Sivaramakrishnan, S.; Schneider, J.L.; Sitikov, A.; Goldman, R.D.; Ridge, K.M. Shear Stress Induced Reorganization of the Keratin Intermediate Filament Network Requires Phosphorylation by Protein Kinase C ζ. Mol. Biol. Cell 2009, 20, 2755–2765. [CrossRef][PubMed] 33. Parker, P.J.; Justilien, V.; Riou, P.; Linch, M.; Fields, A.P. Atypical Protein Kinase Cι as a human and therapeutic target. Biochem. Pharmacol. 2014, 88, 1–11. [CrossRef][PubMed] 34. Linch, M.; Sanz-Garcia, M.; Soriano, E.; Zhang, Y.; Riou, P.; Rosse, C.; Cameron, A.; Knowles, P.; Purkiss, A.; Kjaer, S.; et al. A Cancer-Associated Mutation in Atypical Protein Kinase Cι Occurs in a Substrate-Specific Recruitment Motif. Sci. Signal 2013, 6, ra82. [CrossRef][PubMed] 35. Murray, N.R.; Jamieson, L.; Yu, W.; Zhang, J.; Gökmen-Polar, Y.; Sier, D.; Anastasiadis, P.; Gatalica, Z.; Thompson, E.A.; Fields, A.P. Protein kinase Cι is required for Ras transformation and colon carcinogenesis in vivo. J. Cell Biol. 2004, 164, 797–802. [CrossRef] 36. Regala, R.P.; Weems, C.; Jamieson, L.; Copland, J.A.; Thompson, E.A.; Fields, A.P. Atypical Protein Kinase Cι Plays a Critical Role in Human Lung Cancer Cell Growth and Tumorigenicity. J. Biol. Chem. 2005, 280, 31109–31115. [CrossRef] 37. Villeneuve, C.; Lagoutte, E.; de Plater, L.; Mathieu, S.; Manneville, J.B.; Maître, J.L.; Chavrier, P.; Rossé, C. aPKCi triggers basal extrusion of luminal mammary epithelial cells by tuning contractility and vinculin localization at cell junctions. Proc. Natl. Acad. Sci. USA 2019, 116, 24108–24114. [CrossRef] 38. Grill, S.W.; Gönczy, P.; Stelzer, E.H.K.; Hyman, A.A. Polarity controls forces governing asymmetric spindle positioning in the Caenorhabditis elegans embryo. Nature 2001, 409, 630–633. [CrossRef] 39. Colombo, K.; Grill, S.W.; Kimple, R.J.; Willard, F.S.; Siderovski, D.P.; Gönczy, P. Translation of Polarity Cues into Asymmetric Spindle Positioning in Caenorhabditis elegans Embryos. Science 2003, 300, 1957–1961. [CrossRef] 40. Galli, M.; Muñoz, J.; Portegijs, V.;Boxem, M.; Grill, S.W.; Heck, A.J.R.; VanDen Heuvel, S. aPKC phosphorylates NuMA-related LIN-5 to position the mitotic spindle during asymmetric division. Nat. Cell Biol. 2011, 13, 1132–1138. [CrossRef] 41. Gillard, G.; Nicolle, O.; Brugière, T.; Prigent, S.; Pinot, M.; Michaux, G. Force Transmission between Three Tissues Controls Bipolar Planar Polarity Establishment and Morphogenesis. Curr. Biol. 2019, 29, 1360–1368. [CrossRef] 42. Cetera, M.; Ramirez-San Juan, G.R.; Oakes, P.W.; Lewellyn, L.; Fairchild, M.J.; Tanentzapf, G.; Gardel, M.L.; Horne-Badovinac, S. Epithelial rotation promotes the global alignment of contractile actin bundles during Drosophila egg chamber elongation. Nat. Commun. 2014, 5, 1–12. [CrossRef][PubMed] 43. Ling, C.; Zheng, Y.; Yin, F.; Yu, J.; Huang, J.; Hong, Y.; Wu, S.; Pan, D. The apical transmembrane protein Crumbs functions as a tumor suppressor that regulates Hippo signaling by binding to Expanded. Proc. Natl. Acad. Sci. USA 2010, 107, 10532–10537. [CrossRef][PubMed] 44. Baumgartner, R.; Poernbacher, I.; Buser, N.; Hafen, E.; Stocker, H. The WW domain protein Kibra acts upstream of Hippo in Drosophila. Dev. Cell 2010, 18, 309–316. [CrossRef][PubMed] 45. Chen, C.L.; Gajewski, K.M.; Hamaratoglu, F.; Bossuyt, W.; Sansores-Garcia, L.; Tao, C.; Halder, G. The apical-basal cell polarity determinant Crumbs regulates Hippo signaling in Drosophila. Proc. Natl. Acad. Sci. USA 2010, 107, 15810–15815. [CrossRef][PubMed] Cells 2020, 9, 151 14 of 17

46. Zhao, B.; Li, L.; Lu, Q.; Wang, L.H.; Liu, C.Y.; Lei, Q.; Guan, K.L. is a novel Hippo pathway component that inhibits YAP oncoprotein. Genes Dev. 2011, 25, 51–63. [CrossRef][PubMed] 47. Chan, S.W.; Lim, C.J.; Chong, Y.F.; Pobbati, A.V.; Huang, C.; Hong, W. Hippo pathway-independent restriction of TAZ and YAP by angiomotin. J. Biol. Chem. 2011, 286, 7018–7026. [CrossRef] 48. Wang, W.; Huang, J.; Chen, J. Angiomotin-like proteins associate with and negatively regulate YAP1. J. Biol. Chem. 2011, 286, 4364–4370. [CrossRef] 49. Kim, N.G.; Koh, E.; Chen, X.; Gumbiner, B.M. E- mediates contact inhibition of proliferation through Hippo signaling-pathway components. Proc. Natl. Acad. Sci. USA 2011, 108, 11930–11935. [CrossRef] 50. Schlegelmilch, K.; Mohseni, M.; Kirak, O.; Pruszak, J.; Rodriguez, J.R.; Zhou, D.; Kreger, B.T.; Vasioukhin, V.; Avruch, J.; Brummelkamp, T.R.; et al. Yap1 acts downstream of α-catenin to control epidermal proliferation. Cell 2011, 144, 782–795. [CrossRef] 51. Archibald, A.; Al-Masri, M.; Liew-Spilger, A.; McCaffrey, L. Atypical protein kinase C induces cell transformation by disrupting Hippo/Yap signaling. Mol. Biol. Cell 2015, 26, 3578–3595. [CrossRef] 52. Zhou, P.J.; Xue, W.; Peng, J.; Wang, Y.; Wei, L.; Yang, Z.; Zhu, H.H.; Fang, Y.X.; Gao, W.Q. Elevated expression of Par3 promotes prostate cancer metastasis by forming a Par3/aPKC/KIBRA complex and inactivating the hippo pathway. J. Exp. Clin. Cancer Res. 2017, 36, 139. [CrossRef][PubMed] 53. Sasaki, H. Position- and polarity-dependent Hippo signaling regulates cell fates in preimplantation mouse embryos. Semin. Cell Dev. Biol. 2015, 47, 80–87. [CrossRef][PubMed] 54. Hirate, Y.; Hirahara, S.; Inoue, K.; Kiyonari, H.; Niwa, H.; Sasaki, H. Par-aPKC-dependent and -independent mechanisms cooperatively control cell polarity, Hippo signaling, and cell positioning in 16-cell stage mouse embryos. Dev. Growth Differ. 2015, 57, 544–556. [CrossRef][PubMed] 55. Lee, H.; Kang, J.; Ahn, S.; Lee, J. The Hippo Pathway Is Essential for Maintenance of Apicobasal Polarity in the Growing Intestine of Caenorhabditis elegans. Genetics 2019, 213, 501–515. [CrossRef][PubMed] 56. Kim, N.-G.; Gumbiner, B.M. Adhesion to fibronectin regulates Hippo signaling via the FAK-Src-PI3K pathway. J. Cell Biol. 2015, 210, 503–515. [CrossRef] 57. Lachowski, D.; Cortes, E.; Robinson, B.; Rice, A.; Rombouts, K.; Del Rio Hernandez, A.E. FAK controls the mechanical activation of YAP, a transcriptional regulator required for durotaxis. FASEB J. 2018, 32, 1099–1107. [CrossRef] 58. Zhang, J.; Zhou, Y.; Tang, P.; Cheng, A.; Yu, J.; To, K.; Kang, W. Mechanotransduction and Cytoskeleton Remodeling Shaping YAP1 in Gastric Tumorigenesis. Int. J. Mol. Sci. 2019, 20, 1576. [CrossRef] 59. Fletcher, G.C.; Diaz-de-la-Loza, M.-D.-C.; Borreguero-Muñ oz, N.; Holder, M.; Aguilar-Aragon, M.; Thompson, B.J. Mechanical strain regulates the Hippo pathway in Drosophila. Development 2018, 145, dev159467. [CrossRef] 60. Varelas, X. The Hippo pathway effectors TAZ and YAP in development, homeostasis and disease. Development 2014, 141, 1614–1626. [CrossRef] 61. Rinschen, M.M.; Grahammer, F.; Hoppe, A.K.; Kohli, P.; Hagmann, H.; Kretz, O.; Bertsch, S.; Höhne, M.; Göbel, H.; Bartram, M.P.; et al. YAP-mediated mechanotransduction determines the podocyte’s response to damage. Sci. Signal 2017, 10, 474. [CrossRef] 62. Klapholz, B.; Brown, N.H. Tali—The master of integrin adhesions. J. Cell Sci. 2017, 130, 2435–2446. [CrossRef] [PubMed] 63. Haining, A.; Lieberthal, T.; del Río Hernández, A. Talin: A mechanosensitive molecule in health and disease. FASEB J. 2016, 30, 2073–2085. [CrossRef][PubMed] 64. Calderwood, D.A.; Zent, R.; Grant, R.; Rees, D.J.; Hynes, R.O.; Ginsberg, M.H. The talin head domain binds to integrin β subunit cytoplasmic tails and regulates integrin activation. J. Biol. Chem. 1999, 274, 28071–28074. [CrossRef][PubMed] 65. The interaction of talin with the cell membrane is essential for integrin activation and focal adhesion formation. Proc. Natl. Acad. Sci. USA 2018, 115, 10339–10344. [CrossRef][PubMed] 66. Liang, Y.; Chen, H.; Ji, L.; Du, J.; Xie, X.; Li, X.; Lou, Y. Talin2 regulates breast cancer cell migration and invasion by apoptosis. Oncol. Lett. 2018, 16, 285–293. [CrossRef][PubMed] 67. Qi, L.; Jafari, N.; Li, X.; Chen, Z.; Li, L.; Hytönen, V.; Goult, B.; Zhan, C.; Huang, C. Talin2-mediated traction force drives matrix degradation and cell invasion. J. Cell Sci. 2016, 129, 3661–3674. [CrossRef] 68. McBeath, R.; Pirone, D.M.; Nelson, C.M.; Bhadriraju, K.; Chen, C.S. Cell shape, cytoskeletal tension, and RhoA regulate stem cell lineage commitment. Dev. Cell 2004, 6, 483–495. [CrossRef] Cells 2020, 9, 151 15 of 17

69. Hepler, C.; Gupta, R.K. The expanding problem of adipose depot remodeling and postnatal adipocyte progenitor recruitment. Mol. Cell Endocrinol. 2017, 445, 95–108. [CrossRef] 70. Merrick, D.; Sakers, A.; Irgebay, Z.; Okada, C.; Calvert, C.; Morley, M.P.; Percec, I.; Seale, P. Identification of a mesenchymal progenitor cell hierarchy in adipose tissue. Science 2019, 364, eaav2501. [CrossRef] 71. Spalding, K.L.; Arner, E.; Westermark, P.O.; Bernard, S.; Buchholz, B.A.; Bergmann, O.; Blomqvist, L.; Hoffstedt, J.; Näslund, E.; Britton, T.; et al. Dynamics of fat cell turnover in humans. Nature 2008, 453, 783–787. [CrossRef] 72. Arner, P.; Bernard, S.; Salehpour, M.; Possnert, G.; Liebl, J.; Steier, P.; Buchholz, B.A.; Eriksson, M.; Arner, E.; Hauner, H.; et al. Dynamics of human adipose lipid turnover in health and metabolic disease. Nature 2011, 478, 110–113. [CrossRef][PubMed] 73. Goossens, G.H. The Metabolic Phenotype in Obesity: Fat Mass, Body Fat Distribution, and Adipose Tissue Function. Obes. Facts 2017, 10, 207–215. [CrossRef][PubMed] 74. Shoham, N.; Gefen, A. Mechanotransduction in adipocytes. J. Biomech. 2012, 45, 1–8. [CrossRef][PubMed] 75. Shoham, N.; Gottlieb, R.; Sharabani-Yosef, O.; Zaretsky, U.; Benayahu, D.; Gefen, A. Static mechanical stretching accelerates lipid production in 3T3-L1 adipocytes by activating the MEK signaling pathway. Am. J. Physiol. Cell Physiol. 2012, 302, C429–C441. [CrossRef] 76. Sen, B.; Guilluy, C.; Xie, Z.; Case, N.; Styner, M.; Thomas, J.; Oguz, I.; Rubin, C.; Burridge, K.; Rubin, J. Mechanically induced focal adhesion assembly amplifies anti-adipogenic pathways in mesenchymal stem cells. Stem Cells 2011, 29, 1829–1836. [CrossRef] 77. Che, H.; Yue, J.; Tse, H.F.; Li, G.R. Functional TRPV and TRPM channels in human preadipocytes. Pflug. Arch. 2014, 466, 947–959. [CrossRef] 78. Zhang, Y.; Xie, L.; Gunasekar, S.K.; Tong, D.; Mishra, A.; Gibson, W.J.; Wang, C.; Fidler, T.; Marthaler, B.; Klingelhutz, A.; et al. SWELL1 is a regulator of adipocyte size, insulin signalling and glucose homeostasis. Nat. Cell Biol. 2017, 19, 504–517. [CrossRef] 79. Shoham, N.; Girshovitz, P.; Katzengold, R.; Shaked, N.T.; Benayahu, D.; Gefen, A. Adipocyte stiffness increases with accumulation of lipid droplets. Biophys. J. 2014, 106, 1421–1431. [CrossRef] 80. Pellegrinelli, V.; Heuvingh, J.; du Roure, O.; Rouault, C.; Devulder, A.; Klein, C.; Lacasa, M.; Clément, E.; Lacasa, D.; Clément, K. Human adipocyte function is impacted by mechanical cues. J. Pathol. 2014, 233, 183–195. [CrossRef] 81. Koo, J.H.; Guan, K.L. Interplay between YAP/TAZ and Metabolism. Cell Metab. 2018, 28, 196–206. [CrossRef] 82. Ardestani, A.; Lupse, B.; Maedler, K. Hippo Signaling: Key Emerging Pathway in Cellular and Whole-Body Metabolism. Trends Endocrinol. Metab. 2018, 29, 492–509. [CrossRef][PubMed] 83. Santinon, G.; Pocaterra, A.; Dupont, S. Control of YAP/TAZ Activity by Metabolic and Nutrient-Sensing Pathways. Trends Cell Biol. 2016, 26, 289–299. [CrossRef][PubMed] 84. Wang, W.; Xiao, Z.D.; Li, X.; Aziz, K.E.; Gan, B.; Johnson, R.L.; Chen, J. AMPK modulates Hippo pathway activity to regulate energy homeostasis. Nat. Cell Biol. 2015, 17, 490–499. [CrossRef][PubMed] 85. Croci, O.; De Fazio, S.; Biagioni, F.; Donato, E.; Caganova, M.; Curti, L.; Doni, M.; Sberna, S.; Aldeghi, D.; Biancotto, C.; et al. Transcriptional integration of mitogenic and mechanical signals by Myc and YAP. Genes Dev. 2017, 31, 2017–2022. [CrossRef] 86. Abdesselem, H.; Madani, A.; Hani, A.; Al-Noubi, M.; Goswami, N.; Ben Hamidane, H.; Billing, A.M.; Pasquier, J.; Bonkowski, M.S.; Halabi, N.; et al. SIRT1 Limits Adipocyte Hyperplasia through c-Myc Inhibition. J. Biol. Chem. 2016, 291, 2119–2135. [CrossRef] 87. El Ouarrat, D.; Isaac, R.; Lee, Y.S.; Oh, D.Y.; Wollam, J.; Lackey, D.; Riopel, M.; Bandyopadhyay, G.; Seo, J.B.; Sampath-Kumar, R.; et al. TAZ Is a Negative Regulator of PPARγ Activity in Adipocytes and TAZ Deletion Improves Insulin Sensitivity and Glucose Tolerance. Cell Metab. 2019.[CrossRef] 88. Li, Y.; Du, J.; Zhu, E.; Zhang, J.; Han, J.; Zhao, W.; Sun, B.; Tian, D. Liraglutide suppresses proliferation and induces adipogenic differentiation of 3T3-L1 cells via the Hippo-YAP signaling pathway. Mol. Med. Rep. 2018, 17, 4499–4507. [CrossRef] 89. Nieman, K.M.; Romero, I.L.; Van Houten, B.; Lengyel, E. Adipose tissue and adipocytes support tumorigenesis and metastasis. Biochim. Biophys. Acta 2013, 1831, 1533–1541. [CrossRef] 90. Quail, D.F.; Dannenberg, A.J. The obese adipose tissue microenvironment in cancer development and progression. Nat. Rev. Endocrinol. 2019, 15, 139–154. [CrossRef] Cells 2020, 9, 151 16 of 17

91. Li, H.J.; Fu, J.K.; Che, X.M.; Fan, L.; Zhang, Y.; Bai, E. Obesity accelerates murine gastric cancer growth by modulating the Sirt1/YAP pathway. Oncol. Lett. 2017, 14, 4151–4157. [CrossRef] 92. Wang, C.; Jeong, K.; Jiang, H.; Guo, W.; Gu, C.; Lu, Y.; Liang, J. YAP/TAZ regulates the insulin signaling via IRS1/2 in endometrial cancer. Am. J. Cancer Res. 2016, 6, 996–1010. [PubMed] 93. Qiao, K.; Ning, S.; Wan, L.; Wu, H.; Wang, Q.; Zhang, X.; Xu, S.; Pang, D. LINC00673 is activated by YY1 and promotes the proliferation of breast cancer cells via the miR-515-5p/MARK4/Hippo signaling pathway. J. Exp. Clin. Cancer Res. 2019, 38, 418. [CrossRef][PubMed] 94. Chen, W.; Bai, Y.; Patel, C.; Geng, F. Autophagy promotes triple negative breast cancer metastasis via YAP nuclear localization. Biochem. Biophys. Res. Commun. 2019, 520, 263–268. [CrossRef][PubMed] 95. Roberts, D.L.; Dive, C.; Renehan, A.G. Biological mechanisms linking obesity and cancer risk: New perspectives. Annu. Rev. Med. 2010, 61, 301–316. [CrossRef][PubMed] 96. Sidossis, L.; Kajimura, S. Brown and beige fat in humans: Thermogenic adipocytes that control energy and glucose homeostasis. J. Clin. Investig. 2015, 125, 478–486. [CrossRef][PubMed] 97. Hwang, J.H.; Kim, A.R.; Kim, K.M.; Park, J.I.; Oh, H.T.; Moon, S.A.; Byun, M.R.; Jeong, H.; Kim, H.K.; Yaffe, M.B.; et al. TAZ couples Hippo/Wnt signalling and insulin sensitivity through Irs1 expression. Nat. Commun. 2019, 10, 421. [CrossRef] 98. Tharp, K.M.; Kang, M.S.; Timblin, G.A.; Dempersmier, J.; Dempsey, G.E.; Zushin, P.H.; Benavides, J.; Choi, C.; Li, C.X.; Jha, A.K.; et al. Actomyosin-Mediated Tension Orchestrates Uncoupled Respiration in Adipose Tissues. Cell Metab. 2018, 27, 602–615. [CrossRef] 99. Vollrath, M.A.; Kwan, K.Y.; Corey, D.P. The micromachinery of mechanotransduction in hair cells. Annu. Rev. Neurosci. 2007, 30, 339–365. [CrossRef] 100. Gangatharan, G.; Schneider-Maunoury, S.; Breau, M.A. Role of mechanical cues in shaping neuronal morphology and connectivity. Biol. Cell 2018, 110, 125–136. [CrossRef] 101. Koser, D.E.; Thompson, A.J.; Foster, S.K.; Dwivedy, A.; Pillai, E.K.; Sheridan, G.K.; Svoboda, H.; Viana, M.; Costa, L.D.; Guck, J.; et al. Mechanosensing is critical for axon growth in the developing brain. Nat. Neurosci. 2016, 19, 1592–1598. [CrossRef] 102. Barnes, J.M.; Przybyla, L.; Weaver, V.M. Tissue mechanics regulate brain development, homeostasis and disease. J. Cell Sci. 2017, 130, 71–82. [CrossRef][PubMed] 103. Moeendarbary, E.; Weber, I.P.; Sheridan, G.K.; Koser, D.E.; Soleman, S.; Haenzi, B.; Bradbury, E.J.; Fawcett, J.; Franze, K. The soft mechanical signature of glial scars in the central nervous system. Nat. Commun. 2017, 8, 14787. [CrossRef][PubMed] 104. Lau, P.; Bossers, K.; Janky, R.; Salta, E.; Frigerio, C.S.; Barbash, S.; Rothman, R.; Sierksma, A.S.; Thathiah, A.; Greenberg, D.; et al. Alteration of the microRNA network during the progression of Alzheimer’s disease. EMBO Mol. Med. 2013, 5, 1613–1634. [CrossRef][PubMed] 105. Murphy, M.C.; Jones, D.T.; Jack, C.R., Jr.; Glaser, K.J.; Senjem, M.L.; Manduca, A.; Felmlee, J.P.; Carter, R.E.; Ehman, R.L.; Huston, J., III. Regional brain stiffness changes across the Alzheimer’s disease spectrum. Neuroimage Clin. 2016, 10, 283–290. [CrossRef] 106. Berg, D. Hyperechogenicity of the substantia nigra: Pitfalls in assessment and specificity for Parkinson’s disease. J. Neural Transm. 2011, 118, 453–461. [CrossRef] 107. Yiu, G.; He, Z. Glial inhibition of CNS axon regeneration. Nat. Rev. Neurosci. 2006, 7, 617–627. [CrossRef] 108. Velasco-Estevez, M.; Gadalla, K.K.; Liñan-Barba, N.; Cobb, S.; Dev, K.K.; Sheridan, G.K. Inhibition of Piezo1 attenuates demyelination in the central nervous system. Glia 2019, 1–20. [CrossRef] 109. Pathak, M.M.; Nourse, J.L.; Tran, T.; Hwe, J.; Arulmoli, J.; Dai Trang, T.L.; Bernardis, E.; Flanagan, L.A.; Tombola, F. Stretch-activated ion channel Piezo1 directs lineage choice in human neural stem cells. Proc. Natl. Acad. Sci. USA 2014, 111, 16148–16153. [CrossRef] 110. Hauser, S.L.; Oksenberk, J.R. The Neurobiology of Multiple Review Sclerosis: Genes, Inflammation, and Neurodegeneration. Neuron 2006, 52, 61–76. [CrossRef] 111. You, Y.; Joseph, C.; Wang, C.; Gupta, V.; Liu, S.; Yiannikas, C.; Chua, B.E.; Chitranshi, N.; Shen, T.; Dheer, Y.; et al. Demyelination precedes axonal loss in the transneuronal spread of human neurodegenerative disease. Brain 2019, 142, 426–442. [CrossRef] 112. Stirling, D.P.; Cummins, K.; Wayne Chen, S.R.; Stys, P. Axoplasmic reticulum Ca(2+) release causes secondary degeneration of spinal axons. Ann. Neurol. 2014, 75, 220–229. [CrossRef][PubMed] Cells 2020, 9, 151 17 of 17

113. Velasco-Estevez, M.; Mampay, M.; Boutin, H.; Chaney, A.; Warn, P.; Sharp, A.; Burgess, E.; Moeendarbary, E.; Dev, K.K.; Sheridan, G.K. Infection Augments Expression of Mechanosensing Piezo1 Channels in Amyloid Plaque-Reactive Astrocytes. Front. Aging Neurosci. 2018, 10, 332. [CrossRef][PubMed] 114. Wang, L.; Xia, J.; Li, J.; Hagemann, T.L.; Jones, J.R.; Fraenkel, E.; Weitz, D.A.; Zhang, S.C.; Messing, A.; Feany, M.B. Tissue and cellular rigidity and mechanosensitive signaling activation in Alexander disease. Nat. Commun. 2018, 9, 1899. [CrossRef][PubMed] 115. Hoshino, M.; Qi, M.L.; Yoshimura, N.; Miyashita, T.; Tagawa, K.; Wada, Y.; Enokido, Y.; Marubuchi, S.; Harjes, P.; Arai, N.; et al. Transcriptional repression induces a slowly progressive atypical neuronal death associated with changes of YAP isoforms and p73. J. Cell Biol. 2006, 172, 589–604. [CrossRef] 116. Fujita, K.; Mao, Y.; Uchida, S.; Chen, X.; Shiwaku, H.; Tamura, T.; Ito, H.; Watase, K.; Homma, H.; Tagawa, K.; et al. Developmental YAPdeltaC determines adult pathology in a model of spinocerebellar ataxia type 1. Nat. Commun. 2017, 8, 1864. [CrossRef] 117. Mueller, K.A.; Glajch, K.E.; Huizenga, M.N.; Wilson, R.A.; Granucci, E.J.; Dios, A.M.; Tousley, A.R.; Iuliano, M.; Weisman, E.; LaQuaglia, M.J.; et al. Hippo Signaling Pathway Dysregulation in Human Huntington’s Disease Brain and Neuronal Stem Cells. Sci. Rep. 2018, 8, 11355. [CrossRef] 118. Križaj, D.; Ryskamp, D.A.; Tian, N.; Tezel, G.; Mitchell, C.H.; Slepak, V.Z.; Shestopalov, V.I. From mechanosensitivity to inflammatory responses: New players in the pathology of glaucoma. Curr. Eye Res. 2014, 39, 105–119. [CrossRef] 119. Ryskamp, D.A.; Witkovsky, P.; Barabas, P.; Huang, W.; Koehler, C.; Akimov, N.P.; Lee, S.H.; Chauhan, S.; Xing, W.; Rentería, R.C.; et al. The polymodal ion channel transient receptor potential vanilloid 4 modulates calcium flux, spiking rate, and apoptosis of mouse retinal ganglion cells. J. Neurosci. 2011, 31, 7089–7101. [CrossRef] 120. Alloui, A.; Zimmermann, K.; Mamet, J.; Duprat, F.; Noël, J.; Chemin, J.; Guy, N.; Blondeau, N.; Voilley, N.; Rubat-Coudert, C.; et al. TREK-1, a K+ channel involved in polymodal pain perception. EMBO J. 2006, 25, 2368–2376. [CrossRef] 121. White, J.P.; Cibelli, M.; Urban, L.; Nilius, B.; McGeown, J.G.; Nagy, I. TRPV4: Molecular Conductor of a Diverse Orchestra. Physiol. Rev. 2016, 96, 911–973. [CrossRef] 122. Sharma, S.; Goswami, R.; Rahaman, S.O. The TRPV4-TAZ Mechanotransduction Signaling Axis in Matrix Stiffness- and TGFβ1-Induced Epithelial-Mesenchymal Transition. Cell. Mol. Bioeng. 2019, 12, 139. [CrossRef] [PubMed] 123. Sharma, S.; Goswami, R.; Zhang, D.X.; Rahaman, S.O. TRPV4 regulates matrix stiffness and TGFβ1-induced epithelial-mesenchymal transition. J. Cell. Mol. Med. 2019, 23, 761–774. [CrossRef][PubMed] 124. Liu, B.; McNally, S.; Kilpatrick, J.I.; Jarvis, S.P.; O’Brien, C.J. Aging and ocular tissue stiffness in glaucoma. Surv. Ophthalmol. 2018, 63, 56–74. [CrossRef][PubMed]

© 2020 by the authors. Licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license (http://creativecommons.org/licenses/by/4.0/).